An inducible CiliaGFP mouse model for in vivo visualization and analysis of cilia in live tissue
- Amber K O’Connor†6,
- Erik B Malarkey†1,
- Nicolas F Berbari1,
- Mandy J Croyle1,
- Courtney J Haycraft2,
- P Darwin Bell3,
- Peter Hohenstein4,
- Robert A Kesterson5 and
- Bradley K Yoder1Email author
© O'Connor et al.; licensee BioMed Central Ltd. 2013
Received: 29 April 2013
Accepted: 14 June 2013
Published: 3 July 2013
Cilia are found on nearly every cell type in the mammalian body, and have been historically classified as either motile or immotile. Motile cilia are important for fluid and cellular movement; however, the roles of non-motile or primary cilia in most tissues remain unknown. Several genetic syndromes, called the ciliopathies, are associated with defects in cilia structure or function and have a wide range of clinical presentations. Much of what we know about the formation and maintenance of cilia comes from model systems like C. elegans and Chalmydomonas. Studies of mammalian cilia in live tissues have been hampered by difficulty visualizing them.
To facilitate analyses of mammalian cilia function we generated an inducible CiliaGFP mouse by targeting mouse cDNA encoding a cilia-localized protein somatostatin receptor 3 fused to GFP (Sstr3::GFP) into the ROSA26 locus. In this system, Sstr3::GFP is expressed from the ubiquitous ROSA26 promoter after Cre mediated deletion of an upstream Neo cassette flanked by lox P sites. Fluorescent cilia labeling was observed in a variety of live tissues and after fixation. Both cell-type specific and temporally regulated cilia labeling were obtained using multiple Cre lines. The analysis of renal cilia in anesthetized live mice demonstrates that cilia commonly lay nearly parallel to the apical surface of the tubule. In contrast, in more deeply anesthetized mice the cilia display a synchronized, repetitive oscillation that ceases upon death, suggesting a relationship to heart beat, blood pressure or glomerular filtration.
The ability to visualize cilia in live samples within the CiliaGFP mouse will greatly aid studies of ciliary function. This mouse will be useful for in vivo genetic and pharmacological screens to assess pathways regulating cilia motility, signaling, assembly, trafficking, resorption and length control and to study cilia regulated physiology in relation to ciliopathy phenotypes.
KeywordsSomatostatin receptor 3 ROSA26 locus Inducible transgene In vivo cilia labeling Intravital microscopy
Cilia have essential roles in regulating signaling pathways that control development and normal tissue function (for recent reviews see [1–3]). There are two basic types of cilia. The first is the primary, non-motile cilium that is composed of a ring of nine microtubule doublets ensheathed by a ciliary membrane and found one per cell. The second type is the motile cilium, which has an additional central pair of microtubules and has a synchronized beat that propels fluid. Motile cilia include those in the trachea and ependymal cells of the ventricles in brain.
Cilia are unique sub-domains of the cell comprised of specific proteins and signaling molecules . Several key signaling pathways are now known to be regulated by the cilium, and numerous G-protein coupled receptors, channels and transcription factors specifically localize to the cilium . As such, a group of syndromes, called the ciliopathies, are caused by defects in the structure or function of the cilium. Ciliopathy disease states range from mild, where only one or a few organ systems are affected, such as in Leber’s Congenital Amaurosis, to more severe syndromes involving nearly all organ systems and resulting in perinatal lethality, as seen in Meckel-Grüber Syndrome. Several phenotypes are related specifically to motile cilia defects, such as chronic bronchiectasis, altered left-right body axis specification, infertility and hydrocephalus. Other ciliopathy phenotypes are linked to defects in ciliary signaling or sensory roles leading to blindness, anosmia, polydactyly, obesity or polycystic kidney disease [1–3].
Model organisms, such as Caenorhabditis elegans and Chlamydomonas rheinhardtii, have been used extensively to study ciliary biology. These systems have the advantages of rapid genetic screens and biochemical analysis of cilia proteins, but perhaps most importantly the cilia in these models are readily visible in living samples. As such, these organisms have contributed greatly to our general understanding of cilia formation and maintenance. However, understanding the physiological roles for mammalian cilia in most tissues and the molecular mechanisms behind ciliopathy associated diseases remains a challenge in the field. Unfortunately, to date there have been no inducible, in vivo mammalian models to easily visualize cilia.
To address this limitation, we generated the CiliaGFP mouse that allows direct visualization of mammalian cilia in vivo. Cilia labeling is inducible using Cre recombinase for tissue or cell type specific analysis or the label can be constitutively expressed. We show here the utility of the CiliaGFP mouse for in vivo and ex vivo detection and analysis of cilia. Importantly, we document here a novel finding showing synchronized movement of primary cilia in the kidney of a live mouse that underscores the utility of this model.
Construct generation and mouse engineering
To activate the Cre recombinase in Pdx1CreER animals, mice were injected with 6 mg of tamoxifen every other day over a five-day period and the pancreata were harvested three days after the final injection. Tamoxifen (Sigma-Aldrich, St. Louis, MO T5648) was dissolved in corn oil at 20 mg/ml, and bolus injections of 300 μl were administered intraperitoneally.
Renal tubule isolation
Mice were anesthetized and euthanized, and whole kidneys were isolated and cut into approximately 2 mm pieces. The tissue was incubated at 37°C in three changes of collagenase buffer for 30-minute intervals with gentle agitation every 10 minutes (Collagenase buffer: 10 mg/ml Collagenase Type IV (Sigma #C5138), 50 U/mL DNAse I (Sigma #D5025), and 0.1 mg/ml Soybean Trypsin Inhibitor (Life Technologies, Grand Island, NY #17075-029) in DMEM/F12). After each 30-minute incubation, the supernatant was removed and replaced with fresh collagenase buffer. The supernatants, containing the tubules, were gently pelleted at 100 Relative Centrifugal Force (RCF) for one minute, the tubules were washed three times in phosphate buffered saline (PBS) containing 3% bovine serum albumin (BSA) and pooled. The tubules were kept on ice and imaged live or were fixed in 4% paraformaldehyde (PFA) for five minutes followed by blocking and processing for immunofluorescence analysis.
Ex vivolive imaging
Brains from CiliaGFP EIIa Cre mice were removed after anesthetization and decapitation. The ex vivo brains were cut sagittally down the midline and placed cut surface down on cover glass in room temperature sterile filtered, artificial cerebro-spinal fluid (125 mM NaCl, 2.5 mM KCl, 1.25 mM NaH2PO4, 2 mM CaCl2, 1 mM MgCl2, 25 mM NaHCO3, 25 mM glucose, pH 7.3). Cilia were imaged live using a Hamamatsu C9100-50 EM-CCD camera (Hamamatsu Photonics K.K., Hamamatsu City, Japan) on an inverted Nikon TE2000-U microscope equipped with a 60× Plan Apochromat oil-immersion TIRFM objective (numerical aperture (NA), 1.49; Nikon Instruments Inc., Melville, NY), and a Perkin Elmer Ultraview-ERS 6FE spinning disk confocal module controlled by Volocity 6.2 software (Perkin Elmer, Shelton, CT, USA). Visualization of Sstr3::GFP was accomplished using a fluorescein isothiocyanate (FITC) laser filter set (Chroma Technology, Rockingham, VT, USA); the light source was a 200 mW 488 nm argon laser (Melles Griot, Carlsbad, CA, USA). For immunocytochemistry, we imaged Alexa-594 conjugated antibody staining using a rhodamine/TRITC filter set (Chroma) and 20 mW 568 nm argon krypton laser (Melles Griot), Alexa-647 conjugated antibody staining using a Cy5 filter set (Qioptiq Inc., Fairport, NY) and 15 mW 640 nm diode laser (Melles Griot), Hoechst staining using a 4',6-diamidino-2-phenylindole (DAPI) filter set (Chroma) and 15 mW 405 nm diode laser (Qioptiq).
In vivoanalysis of renal cilia
A group of 8- to 16-week-old mice were anesthetized by intraperitoneal injection of 2.5% tribromoethanol (Sigma T48402). A dorsal incision was made just rostral to the iliac crest and the kidney was gently teased out through the opening, making sure not to damage the renal artery, vein or ureter. The mouse was placed, incision side down, inside a heated chamber maintained at 37°C (LiveCell™ Stage Top Incubation System #05-11-0035, Pathology Devices, Inc., Westminster, MD, USA) with the kidney positioned on a coverslip bathed in PBS. The mice were continuously administered isoflurane at 1 to 2% (VetOne Boise, ID#13985-030-60) throughout the procedure and were euthanized after imaging.
Tissue isolation and sectioning
Fresh tissues were isolated and processed as described in . For immunofluorescence detection of neuronal cilia, animals were anesthetized with 2.5% tribromoethanol (Sigma T48402), and transcardially perfused with PBS, followed by 4% PFA. The brain was then isolated and processed in the same manner as other tissues. Tissues were dissected into PBS, fixed in 4% PFA overnight at 4°C, saturated with 30% sucrose in PBS, oriented in optimal cutting temperature compound (Fisher Scientific, Pittsburgh, PA #14-373-65), and frozen in a dry ice-ethanol bath. Sections 10 to 15 μM thick were cut and mounted onto slides, fixed again in 4% PFA for five minutes at room temperature (RT) and then used for immunofluorescence staining. Sperm were collected by removing epididymides and incubating in Whittens-HEPES buffer (100 NaCl, 4.4 KCl, 1.2 KH2PO4, 1.2 Mg SO4, 5.4 glucose, 0.8 pyruvate, 4.8 lactate, 20 HEPES in mM) for 10 minutes and then capacitated by incubation in Whittens-HEPES supplemented with 15 mM NaHCO3 and 5 mg/ml BSA for 1 hour.
For immunofluorescence detection of cilia, staining was performed as in . Briefly, cryosections were blocked in PBS+ (1% BSA, 1% Normal Donkey Serum, in PBS + 0.1% Triton-X 100) for 30 minutes. Primary and secondary antibodies were diluted in blocking solution and applied to sections for one hour at RT or overnight at 4°C. After incubation, the slides were washed in PBS three times for five minutes each before being stained with Hoechst, and mounted with 1,4-diazabicyclo[2.2.2]octane (DABCO). The following primary antibodies were used: acetylated α-tubulin (Sigma T7451, 1 mg/ml input) pre-conjugated to AlexaFluor 647 (Life Technologies #A-20186) and used at 1:2,000, Adenylyl cyclase III (ACIII, Santa Cruz Biotechnology, Santa Cruz, CA, USA, #sc-11617) used at 1:500, and Arl13b (a gift from Dr. Tamara Caspary at Emory University) used at 1:2,000. The following secondary antibodies were used: anti-goat and anti-rabbit AlexaFluor-594 each used at 1:1,000.
For isolated tubules, immediately upon isolation the tubules were fixed in 4% PFA for 5 minutes followed by blocking in PBS+ for 30 minutes. Tubules were incubated with the direct conjugated acetylated α-tubulin antibody for 30 minutes at RT and washed in PBS for 5 minutes. Nuclei were stained with Hoechst (Sigma #33258), and imaged in PBS or 50% glycerol droplets on cover glass.
Results and discussion
CiliaGFP mice were engineered to express the cilia localized somatostatin receptor 3 protein fused with green fluorescent protein (Sstr3::GFP). Since the construct was targeted into the ubiquitously expressed ROSA26 locus it should permit labeling of cilia in nearly every tissue or cell type in the body depending on the Cre line used to delete the floxed Neomycin cassette (Figure 1). The utility of the CiliaGFP model was assessed using ubiquitous and cell type-specific Cre lines in fixed tissue, in live ex vivo samples, and in situ in the context of living animals. In Cre negative control animals (CiliaGFP-OFF/WT;Cre-) no GFP labeling was evident (Additional file 1: Figure S1A-C). However, it should be noted that the level of activation of the ROSA26 locus has been reported to decrease in postnatal animals, and to show minimal activation in a few cell types, such as astrocytes , which may impact the utility of this mouse model in certain circumstances.
The ependymal cells lining the ventricles are important for movement of cerebral spinal fluid and defects in their motility are associated with hydrocephalus [14, 15]. Interestingly, the clinical importance of primary cilia in the brain has recently become apparent, despite a general lack of understanding of their function [1, 16]. On neurons, disruption of the primary cilium or ciliary proteins revealed that they have an important role in regulating satiation and object recognition through unknown mechanisms [16–18]. In addition, cilia are known to be important for sight and smell [16, 19–21] and recently it was demonstrated that they regulate pathways involved in adult neurogenesis and migration of newborn neurons . However, the ubiquitous nature of primary cilia on most neurons in the central nervous system (CNS) was unexpected . While the most common method of cilia visualization in mammals relies on antibodies against post-translationally modified forms of tubulin, such as acetylated α-tubulin, or polyglutamylated tubulin, these methods prove especially challenging in the brain since tubulin throughout neuronal processes and cell bodies are highly post-translationally modified . This has made visualizing cilia on neurons difficult without special fixation and perfusion conditions, thus this new cilia label mouse model will simplify and streamline studies of neuronal cilia.
Time-lapse live imaging was performed on the ependymal cells to explore the potential utility of the CiliaGFP mouse in cilia motility studies. Images were captured at 15 frames per second, and clear and distinct cilia could be seen (Additional file 2, see Methods). All of these cilia were visualized in live samples immediately after isolation with little or no preparation and no counterstaining (Figure 2A-C, and Additional file 2).
In addition to live imaging, the GFP label was easily visible after fixation and subsequent immunofluorescence staining with markers used to confirm that Sstr3::GFP labels cilia. In the lining of the lateral ventricle of CiliaGFP-ON CiliaGFP mice, Sstr3::GFP and acetylated α-tubulin co-localize within many of the ependymal cells and in the primary cilia of neighboring cells (Figure 2D). Interestingly, the primary cilia labeling is somewhat brighter than it is on the motile ependymal cilia; this is likely due to the increased number of cilia resulting in greater membrane surface area within which the Sstr3::GFP label can become diluted. This has been observed for the hedgehog pathway mediator, Smoothened, in cells induced to form multiple primary cilia . Similar primary cilia staining was observed in the pituitary (Figure 2E); and in the hindbrain region (Figure 2F) where the GFP signal co-localized with acetylated α-tubulin and the neuronal cilia marker ACIII, respectively. Together these images, as well as those in the living samples, demonstrate that the expression levels in the brain are sufficient to facilitate studies of neuronal cilia. For example, this model would facilitate the analysis of the prevalence of cilia, differences in cilia morphology, or assessment of the efficiency of cilia ablation in specific brain regions (for example, after Cre deletion of a floxed ciliary allele). Also, this model would enhance studies requiring live tissues, such as the measurement of ligand induced translocation of proteins into and out of the cilium, in electrophysiology to patch ciliated neurons or even the cilium itself, or in pharmacological studies of factors regulating cilia length dynamics in the brain.
In kidney sections, in live isolated tubules, and in vivo , GFP-labeled cilia were readily identifiable (Figure 3A-C). Again the label was seen without fixation or staining and persisted throughout handling and imaging. In isolated tubules, many cilia remained attached through isolation, fixation, staining and imaging (Figure 3D). However, some GFP labeled debris was observed in the isolated tubules that are likely to be ciliary fragments broken off during isolation. These fragments were not observed in the imaging of intact kidneys. Again, the specificity of ciliary localization was confirmed in tubules and in sections using acetylated α-tubulin (Figure 3D, E).
Another interesting observation made in 5 out of 11 mice analyzed was that the cilia within a nephron would oscillate back and forth within the tubular lumen (Figure 4A, B and Additional file 4). This oscillation was rapid (4.58 ± 0.2 Hz, Figure 4D) and could be captured using relatively high speed image acquisition (approximately 26 fps). The sweep of the cilium during oscillation was irregular, where during each oscillation the cilium would spend the majority of the time bent along the tubule wall compared to any other point of its sweep (Figure 4C, E). These oscillations are most likely passive and not a result of molecular motors, such as dynein, as there is no evidence that these primary cilia have the machinery necessary for active motility . In addition, the frequency of oscillation is similar to that documented for mouse heart rates under anesthesia . Also, the presence of this oscillatory motion would change in the same animal over time, either appearing or disappearing during the course of the experiment, which suggests that the movement may be elicited by the depth of anesthesia, heart rate, stroke volume, blood pressure and their impact on glomerular filtration; however, we were unable to simultaneously measure the heart rate of mice while imaging. Furthermore, most of the cilia in a whole field move in unison, suggesting regulation at the level of the whole kidney, not at the level of the individual cells/tubules/glomeruli. Additional evidence supporting a passive mechanism is that the movement of the cilium in the tubules stops almost immediately upon death and the cilia extend nearly perpendicularly into the nephron lumen (Additional file 5, N = 2). Together these data suggest that tubular flow is not constant. Regular periodic oscillation in the flow rate of glomerular filtrate has been documented using fluorescent dextran  along with observations of oscillation in proximal tubular pressure . This pulsatile flow rate in the proximal tubules provides a mechanism for the oscillation of cilia that we observe and also explains why the cilia spend a large proportion of each oscillatory sweep bent in the downstream position.
An alternate explanation is that the cilia, at least in the proximal tubule images captured here, are not passive but actually exhibit motile behavior. It should be noted that some studies have found that cilia in the node of the gastrulation stage mouse embryo have a 9 + 0 structure (similar to the kidney) and have a rotational motility that is distinct from the waveform motion of cilia on ependymal or tracheal cells [41, 42]. However, others studies have reported that the node has a second form of cilia that has a 9 + 2 arrangement and it is not clear which form is actually responsible for the rotational beating . Follow-up studies will be necessary to conclusively determine the cause of the ciliary oscillation which could impact our understanding of ciliopathy disorders, such as polycystic kidney disease.
To determine if the CiliaGFPmouse would be sufficient to analyze the photoreceptor CC, we evaluated the retinas of EIIa Cre; CiliaGFP mice. Interestingly, the ganglion cells of the retina contained many ciliated cells (Figure 5B) as did many of the cells in the anterior region of the inner nuclear layer (INL, Figure 5C). GFP was concentrated in the CC of the photoreceptors but is detectable in the outer segments (Figure 5D, Additional file 1: Figure S1F). In addition, rhodopsin staining indicated that the CiliaGFP label does not overtly interrupt trafficking of rhodopsin or affect the health of the outer segment (Additional file 1: Figure S1F). Finally, attempting to label the cilia in the retina with ciliary markers, such as Arl13b and acetylated α-tubulin, frequently requires antigen retrieval and can be challenging using standard immunofluorescence protocols (Figure 5, acetylated α-tubulin in purple). Thus, the CiliaGFP mouse will be useful for identifying the connecting cilia in the retina of live mice, and in samples without relying on antibody staining approaches.
Spatial and temporal control of expression
In addition to cell-type specific control of Sstr3::GFP expression, we could also induce expression at a specific time point in the life of a mouse. To demonstrate temporal control of the CiliaGFP allele, we used the tamoxifen responsive Pdx1 Cre ER line. In adult mice, Pdx1 Cre ER is expressed in the β-cells of the pancreas. We harvested pancreata from mice three days after a series of tamoxifen injections (see Methods) and processed them for immunofluorescence. As shown in Figure 6E, many of the cilia in the islets were labeled with Sstr3::GFP. Primary cilia are present on islet cells and in the ducts of the pancreas as reported previously [49, 50], and in agreement with known Pdx1 Cre expression, only the islets were labeled in these mice (Figure 6E). Specificity was confirmed with acetylated α-tubulin staining (Figure 6E) and the absence of Sstr3::GFP in the ducts as well as in animals lacking the Cre transgene animals was confirmed (Additional file 1: Figure S1A).
Generation of the constitutively expressed CiliaGFP-ONallele
Here we have developed a new tool for in vivo and ex vivo detection and visualization of mammalian cilia, the CiliaGFP mouse. We have demonstrated that the CiliaGFP mouse is functional, cilia specific, and that spatial and temporal control of expression is possible. In animals without Cre or without tamoxifen, no ciliary label was detected (Additional file 1: Figure S1A-C). In addition, there were a few tissues where ciliary labeling was not easily observable, such as the trachea and the motile cilia in the oviduct (Additional file 1: Figure S1D, E) of CiliaGFP-ON mice. The cilia in these regions contained GFP but at a similar level as the rest of the cell membrane. The reason that cilia in these regions of the CiliaGFP mouse were not highly labeled is unknown but it could be a result of the oviduct and tracheal epithelial cells having many more cilia per cell (approximately 150, Additional file 1: Figure S1D and E)  than ependymal cells (approximately 15 per cell, Figure 2B)  or choroid plexus cells (approximately 5 per cell, Figure 2C). Which might result in the dilution of the GFP signal among an increased number of cilia as has been shown for Smoothened in multi-ciliated cells .
Another caveat to using the CiliaGFP mouse is that when the CiliaGFP-ON allele is expressed in the testes, sperm from CiliaGFP-ON males have impaired motility likely due to the localization of Sstr3::GFP in the flagella. This does raise the possibility that Sstr3 may be altering the function or motility of cilia in other tissues as well. This is an important factor to consider since a recent study has shown that over-expressing GPCRs like Sstr3 in cilia could affect the normal distribution of ciliary proteins and cilia morphology . Aside from these exceptions, this mouse will facilitate the study of cilia in tissues where staining and imaging have been difficult, such as the brain and eye, and for studies that require live or in situ analysis.
There are multiple uses for this mouse model: for example, mammalian mutagenesis and in vivo pharmacological screens for factors that affect ciliogenesis, cilia length control and ciliary protein trafficking; to assess recovery of ciliary proteins by FRAP analysis; to analyze regulation of cilia motility; or to screen for suppressor mutations using known cilia mutants and assessing the restoration of ciliogenesis. Further, the CiliaGFPmouse can be used for assessing cilia loss when used in conjunction with floxed alleles of genes required for ciliogenesis, since Cre expression would simultaneously delete the floxed gene required for ciliogenesis and remove the floxed-stop cassette to induce Sstr3::GFP expression. Lastly, we have shown the utility of this model with in situ documentation of ciliary motion in the tubules of the kidney. Indeed, this observation indicates the CiliaGFP mouse will be useful for in vivo mechanosensory studies that may provide important insights into how cilia dysfunction contributes to cyst development.
Adenylate cyclase III
Bovine serum albumin
Central nervous system
Adenovirus early transcription region II DNA binding protein promoter
- ES cells:
Embryonic stem cells
Green fluorescent protein
Inner nuclear layer
Pancreatic and Duodenal Homeobox 1
Relative Centrifugal Force
Reverse oriented splice acceptor β-galactosidase/neomycin 26
Somatostatin receptor 3
We would like to acknowledge the UAB Transgenic Animal/Embryonic Stem Cell Facility for assistance with generating the CiliaGFP mouse, and Kevin J. Vanderwall for providing the illustration Figure 5D. AKO was supported byT32 AR047512. This work was supported by NIH R01 DK065655 to BKY and by the UAB Hepatorenal Fibrocystic Kidney Disease Core Center (UAB RPKDCC, P30 DK074038).
- Oh EC, Katsanis N: Cilia in vertebrate development and disease. Development. 2012, 139: 443-448. 10.1242/dev.050054.View ArticleGoogle Scholar
- Pazour GJ, Witman GB: The vertebrate primary cilium is a sensory organelle. Curr Opin Cell Biol. 2003, 15: 105-110. 10.1016/S0955-0674(02)00012-1.View ArticleGoogle Scholar
- Davenport JR, Yoder BK: An incredible decade for the primary cilium: a look at a once-forgotten organelle. Am J Physiol Renal Physiol. 2005, 289: F1159-F1169. 10.1152/ajprenal.00118.2005.View ArticleGoogle Scholar
- Berbari NF, O'Connor AK, Haycraft CJ, Yoder BK: The primary cilium as a complex signaling center. Curr Biol. 2009, 19: R526-R535. 10.1016/j.cub.2009.05.025.View ArticleGoogle Scholar
- Hohenstein P, Slight J, Ozdemir DD, Burn SF, Berry R, Hastie ND: High-efficiency Rosa26 knock-in vector construction for Cre-regulated overexpression and RNAi. Pathogenetics. 2008, 1: 3-10.1186/1755-8417-1-3.View ArticleGoogle Scholar
- Nagy A: Manipulating the Mouse Embryo: a Laboratory Manual. 2003, Cold Spring Harbor, NY: Cold Spring Harbor Laboratory Press, 764-3Google Scholar
- O’Connor AK, Kesterson RA, Yoder BK: Generating conditional mutants to analyze ciliary functions: the use of Cre-lox technology to disrupt cilia in specific organs. Methods Cell Biol. 2009, 93: 305-330.View ArticleGoogle Scholar
- Lakso M, Pichel JG, Gorman JR, Sauer B, Okamoto Y, Lee E, Alt FW, Westphal H: Efficient in vivo manipulation of mouse genomic sequences at the zygote stage. Proc Natl Acad Sci U S A. 1996, 93: 5860-5865. 10.1073/pnas.93.12.5860.View ArticleGoogle Scholar
- Xu AW, Kaelin CB, Takeda K, Akira S, Schwartz MW, Barsh GS: PI3K integrates the action of insulin and leptin on hypothalamic neurons. J Clin Invest. 2005, 115: 951-958.View ArticleGoogle Scholar
- Zhang H, Fujitani Y, Wright CV, Gannon M: Efficient recombination in pancreatic islets by a tamoxifen-inducible Cre-recombinase. Genesis. 2005, 42: 210-217. 10.1002/gene.20137.View ArticleGoogle Scholar
- Berbari NF, Johnson AD, Lewis JS, Askwith CC, Mykytyn K: Identification of ciliary localization sequences within the third intracellular loop of G protein-coupled receptors. Mol Biol Cell. 2008, 19: 1540-1547. 10.1091/mbc.E07-09-0942.View ArticleGoogle Scholar
- Croyle MJ, Lehman JM, O'Connor AK, Wong SY, Malarkey EB, Iribarne D, Dowdle WE, Schoeb TR, Verney ZM, Athar M, Michaud EJ, Reiter JF, Yoder BK: Role of epidermal primary cilia in the homeostasis of skin and hair follicles. Development. 2011, 138: 1675-1685. 10.1242/dev.060210.View ArticleGoogle Scholar
- Anthony TE, Klein C, Fishell G, Heintz N: Radial glia serve as neuronal progenitors in all regions of the central nervous system. Neuron. 2004, 41: 881-890. 10.1016/S0896-6273(04)00140-0.View ArticleGoogle Scholar
- Banizs B, Pike MM, Millican CL, Ferguson WB, Komlosi P, Sheetz J, Bell PD, Schwiebert EM, Yoder BK: Dysfunctional cilia lead to altered ependyma and choroid plexus function, and result in the formation of hydrocephalus. Development. 2005, 132: 5329-5339. 10.1242/dev.02153.View ArticleGoogle Scholar
- Nakamura Y, Sato KY: Role of disturbance of ependyaml ciliary function in development of hydrocephalus in rats. Childs Nerv Syst. 1993, 9: 65-71. 10.1007/BF00305310.View ArticleGoogle Scholar
- Sharma N, Berbari NF, Yoder BK: Ciliary dysfunction in developmental abnormalities and diseases. Curr Top Dev Biol. 2008, 85: 371-427.View ArticleGoogle Scholar
- Davenport JR, Watts AJ, Roper VC, Croyle MJ, van Groen T, Wyss JM, Nagy TR, Kesterson RA, Yoder BK: Disruption of intraflagellar transport in adult mice leads to obesity and slow-onset cystic kidney disease. Curr Biol. 2007, 17: 1586-1594. 10.1016/j.cub.2007.08.034.View ArticleGoogle Scholar
- Doherty D: Joubert syndrome: insights into brain development, cilium biology, and complex disease. Semin Pediatr Neurol. 2009, 16: 143-154. 10.1016/j.spen.2009.06.002.View ArticleGoogle Scholar
- Pazour GJ, Baker SA, Deane JA, Cole DG, Dickert BL, Rosenbaum JL, Witman GB, Besharse JC: The intraflagellar transport protein, IFT88, is essential for vertebrate photoreceptor assembly and maintenance. J Cell Biol. 2002, 157: 103-113. 10.1083/jcb.200107108.View ArticleGoogle Scholar
- Kulaga HM, Leitch CC, Eichers ER, Badano JL, Lesemann A, Hoskins BE, Lupski JR, Beales PL, Reed RR, Katsanis N: Loss of BBS proteins causes anosmia in humans and defects in olfactory cilia structure and function in the mouse. Nat Genet. 2004, 36: 994-998. 10.1038/ng1418.View ArticleGoogle Scholar
- McIntyre JC, Davis EE, Joiner A, Williams CL, Tsai IC, Jenkins PM, McEwen DP, Zhang L, Escobado J, Thomas S, Szymanska K, Johnson CA, Beales PL, Green ED, Mullikin JC, Comparative Sequencing Program NISC, Sabo A, Muzny DM, Gibbs RA, Attié-Bitach T, Yoder BK, Reed RR, Katsanis N, Martens JR: Gene therapy rescues cilia defects and restores olfactory function in a mammalian ciliopathy model. Nat Med. 2012, 18: 1423-1428. 10.1038/nm.2860.View ArticleGoogle Scholar
- Louvi A, Grove EA: Cilia in the CNS: the quiet organelle claims center stage. Neuron. 2011, 69: 1046-1060. 10.1016/j.neuron.2011.03.002.View ArticleGoogle Scholar
- Bishop GA, Berbari NF, Lewis J, Mykytyn K: Type III adenylyl cyclase localizes to primary cilia throughout the adult mouse brain. J Comp Neurol. 2007, 505: 562-571. 10.1002/cne.21510.View ArticleGoogle Scholar
- Fukushima N, Furuta D, Hidaka Y, Moriyama R, Tsujiuchi T: Post-translational modifications of tubulin in the nervous system. J Neurochem. 2009, 109: 683-693. 10.1111/j.1471-4159.2009.06013.x.View ArticleGoogle Scholar
- Mahjoub MR, Stearns T: Supernumerary centrosomes nucleate extra cilia and compromise primary cilium signaling. Curr Biol. 2012, 22: 1628-1634. 10.1016/j.cub.2012.06.057.View ArticleGoogle Scholar
- Praetorius HA, Spring KR: Bending the MDCK cell primary cilium increases intracellular calcium. J Membr Biol. 2001, 184: 71-79. 10.1007/s00232-001-0075-4.View ArticleGoogle Scholar
- Nauli SM, Kawanabe Y, Kaminski JJ, Pearce WJ, Ingber DE, Zhou J: Endothelial cilia are fluid shear sensors that regulate calcium signaling and nitric oxide production through polycystin-1. Circulation. 2008, 117: 1161-1171. 10.1161/CIRCULATIONAHA.107.710111.View ArticleGoogle Scholar
- Guadiana SM, Semple-Rowland S, Daroszewski D, Madorsky I, Breunig JJ, Mykytyn K, Sarkisian MR: Arborization of dendrites by developing neocortical neurons is dependent on primary cilia and type 3 adenylyl cyclase. J Neurosci. 2013, 33: 2626-2638. 10.1523/JNEUROSCI.2906-12.2013.View ArticleGoogle Scholar
- Hoey DA, Downs ME, Jacobs CR: The mechanics of the primary cilium: an intricate structure with complex function. J Biomech. 2012, 45: 17-26. 10.1016/j.jbiomech.2011.08.008.View ArticleGoogle Scholar
- Rydholm S, Zwartz G, Kowalewski JM, Kamali-Zare P, Frisk T, Brismar H: Mechanical properties of primary cilia regulate the response to fluid flow. Am J Physiol Renal Physiol. 2010, 298: F1096-F1102. 10.1152/ajprenal.00657.2009.View ArticleGoogle Scholar
- Downs ME, Nguyen AM, Herzog FA: Hoey DA. 2012, Jacobs CR: An experimental and computational analysis of primary cilia deflection under fluid flow. Comput Methods Biomech Biomed Engin, [Epub ahead of print.]Google Scholar
- Schwartz EA, Leonard ML, Bizios R, Bowser SS: Analysis and modeling of the primary cilium bending response to fluid shear. Am J Physiol. 1997, 272: F132-F138.Google Scholar
- Young YN, Downs M, Jacobs CR: Dynamics of the primary cilium in shear flow. Biophys J. 2012, 103: 629-639. 10.1016/j.bpj.2012.07.009.View ArticleGoogle Scholar
- Shiba D, Yamaoka Y, Hagiwara H, Takamatsu T, Hamada H, Yokoyama T: Localization of Inv in a distinctive intraciliary compartment requires the C-terminal ninein-homolog-containing region. J Cell Sci. 2009, 122: 44-54. 10.1242/jcs.037408.View ArticleGoogle Scholar
- Shiba D, Manning DK, Koga H, Beier DR, Yokoyama T: Inv acts as a molecular anchor for Nphp3 and Nek8 in the proximal segment of primary cilia. Cytoskeleton (Hoboken). 2010, 67: 112-119.Google Scholar
- Ghossoub R, Molla-Herman A, Bastin P, Benmerah A: The ciliary pocket: a once-forgotten membrane domain at the base of cilia. Biol Cell. 2011, 103: 131-144. 10.1042/BC20100128.View ArticleGoogle Scholar
- Ostrowski LE, Dutcher SK, Lo CW: Cilia and models for studying structure and function. Proc Am Thorac Soc. 2011, 8: 423-429. 10.1513/pats.201103-027SD.View ArticleGoogle Scholar
- Hart CY, Burnett JC, Redfield MM: Effects of avertin versus xylazine-ketamine anesthesia on cardiac function in normal mice. Am J Physiol Heart Circ Physiol. 2001, 281: H1938-H1945.Google Scholar
- Kang JJ, Toma I, Sipos A, McCulloch F, Peti-Peterdi J: Quantitative imaging of basic functions in renal (patho)physiology. Am J Physiol Renal Physiol. 2006, 291: F495-F502. 10.1152/ajprenal.00521.2005.View ArticleGoogle Scholar
- Ditlevsen S, Yip KP, Holstein-Rathlou NH: Parameter estimation in a stochastic model of the tubuloglomerular feedback mechanism in a rat nephron. Math Biosci. 2005, 194: 49-69. 10.1016/j.mbs.2004.12.007.View ArticleGoogle Scholar
- Nonaka S, Tanaka Y, Okada Y, Takeda S, Harada A, Kanai Y, Kido M, Hirokawa N: Randomization of left-right asymmetry due to loss of nodal cilia generating leftward flow of extraembryonic fluid in mice lacking KIF3B motor protein. Cell. 1998, 95: 829-837. 10.1016/S0092-8674(00)81705-5. Erratum in: Cell 1999, 99:117View ArticleGoogle Scholar
- Essner JJ, Vogan KJ, Wagner MK, Tabin CJ, Yost HJ, Brueckner M: Conserved function for embryonic nodal cilia. Nature. 2002, 418: 37-38. 10.1038/418037a.View ArticleGoogle Scholar
- Caspary T, Larkins CE, Anderson KV: The graded response to Sonic Hedgehog depends on cilia architecture. Dev Cell. 2007, 12: 767-778. 10.1016/j.devcel.2007.03.004.View ArticleGoogle Scholar
- Fan Y, Esmail MA, Ansley SJ, Blacque OE, Boroevich K, Ross AJ, Moore SJ, Badano JL, May-Simera H, Compton DS, Green JS, Lewis RA, van Haelst MM, Parfrey PS, Baillie DL, Beales PL, Katsanis N, Davidson WS, Leroux MR: Mutations in a member of the Ras superfamily of small GTP-binding proteins causes Bardet-Biedl syndrome. Nat Genet. 2004, 36: 989-993. 10.1038/ng1414.View ArticleGoogle Scholar
- Roepman R, Letteboer SJ, Arts HH, van Beersum SE, Lu X, Krieger E, Ferreira PA, Cremers FP: Interaction of nephrocystin-4 and RPGRIP1 is disrupted by nephronophthisis or Leber congenital amaurosis-associated mutations. Proc Natl Acad Sci U S A. 2005, 102: 18520-18525. 10.1073/pnas.0505774102.View ArticleGoogle Scholar
- Liu X, Udovichenko IP, Brown SD, Steel KP, Williams DS: Myosin VIIa participates in opsin transport through the photoreceptor cilium. J Neurosci. 1999, 19: 6267-6274.Google Scholar
- Fliegauf M, Horvath J, von Schnakenburg C, Olbrich H, Müller D, Thumfart J, Schermer B, Pazour GJ, Neumann HP, Zentgraf H, Benzing T, Omran H: Nephrocystin specifically localizes to the transition zone of renal and respiratory cilia and photoreceptor connecting cilia. J Am Soc Nephrol. 2006, 17: 2424-2433. 10.1681/ASN.2005121351.View ArticleGoogle Scholar
- Berbari NF, Pasek RC, Malarkey EB, Yazdi SM, McNair AD, Lewis WR, Nagy TR, Kesterson RA, Yoder BK: Leptin resistance is a secondary consequence of the obesity in ciliopathy mutant mice. Proc Natl Acad Sci U S A. 2013, 110: 7796-7801. 10.1073/pnas.1210192110.View ArticleGoogle Scholar
- Hebrok M, Kim SK, St Jacques B, McMahon AP, Melton DA: Regulation of pancreas development by hedgehog signaling. Development. 2000, 127: 4905-4913.Google Scholar
- Zhang Q, Davenport JR, Croyle MJ, Haycraft CJ, Yoder BK: Disruption of IFT results in both exocrine and endocrine abnormalities in the pancreas of Tg737(orpk) mutant mice. Lab Invest. 2005, 85: 45-64. 10.1038/labinvest.3700207.View ArticleGoogle Scholar
- Kunimoto K, Yamazaki Y, Nishida T, Shinohara K, Ishikawa H, Hasegawa T, Okanoue T, Hamada H, Noda T, Tamura A, Tsukita S, Tsukita S: Coordinated ciliary beating requires Odf2-mediated polarization of basal bodies via basal feet. Cell. 2012, 148: 189-200. 10.1016/j.cell.2011.10.052.View ArticleGoogle Scholar
- Nishimura Y, Kurisaki A, Nakanishi M, Ohnuma K, Ninomiya N, Komazaki S, Ishiura S, Asashima M: Inhibitory Smad proteins promote the differentiation of mouse embryonic stem cells into ependymal-like ciliated cells. Biochem Biophys Res Commun. 2010, 401: 1-6. 10.1016/j.bbrc.2010.08.099.View ArticleGoogle Scholar
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